Method  for Creating Perfusable Microvessel Systems

ABSTRACT

A method for creating networks of perfusable microvessels in vitro. A mandrel is drawn through a matrix to form a channel through the matrix. Cells are injected into the channel. The matrix is incubated to allow the cells to attach inside the channel. The channel is perfused to remove unattached cells to create a parent vessel, where the parent vessel includes a perfusable hollow channel lined with cells in the matrix. The parent vessel is induced to create sprouts into the surrounding matrix gel so as to form a microvessel network. The microvessel network is subjected to luminal perfusion through the parent vessel.

RELATED APPLICATION

This application claims priority from and is a continuation-in-part of co-pending U.S. application Ser. No. 11/388,920 of Neumann, filed Mar. 24, 2006, entitled “Method for Creating Perfusable Microvessel Systems.” U.S. application Ser. No. 11/388,920 of Neumann is hereby incorporated by reference.

STATEMENT REGARDING FEDERALLY SPONSORED RESEARCH

This invention was made with government support under Grant No. 1 R21 HL081152-01 awarded by NIH National Heart, Lung, and Blood Institute. The government has certain rights in the invention.

FIELD OF THE INVENTION

The present invention relates to methods for the study of physiological and pathological vascular growth, and vascular growth in response to angiogenic or angiostatic factors.

TECHNICAL BACKGROUND

During normal processes of vascular growth (e.g., the menstrual cycle, placentation, changes in adiposity, wound repair, inflammation), the creation of new blood vessels is regulated and eventually ceases. Significantly, the deregulation of vascular growth is a critical element of pathology. For example, tumor growth, diabetic retinopathies, arthritis, and psoriasis involve excessive proliferation of blood vessels that contributes directly to the pathological state. In contrast, impairment of vascular growth, characteristic of aged individuals, compromises the healing of wounds and the revascularization of tissues rendered ischemic by trauma or disease. Therefore, an understanding of the mechanisms that direct the assembly new blood vessels, and the processes that start and stop vascular growth, are central to the development of strategies to control vascularization in disease.

During the growth of new blood vessels (angiogenesis) sprouts arise from endothelial cells that line the lumens of capillaries and postcapillary venules—the smallest branches of the vascular system. Angiogenesis is a complex, multi-step process. Although published studies of angiogenesis number in the many thousands, the cellular mechanisms that mediate and regulate angiogenic growth and morphogenesis are poorly understood.

The details of angiogenic sprouting are difficult to observe in “real-time” in vivo because of the opacity of most tissues. Tissue sections are difficult to reconstruct in 3D and do not communicate the dynamic nature of vascular growth. Moreover, the region near the tips of angiogenic sprouts—a critical area of control of vascular invasion and morphogenesis—is rarely found in tissue sections. In order to overcome the limitations of conventional histology, a variety of “models” of angiogenesis in vivo and in vitro have been developed.

Models of angiogenesis in vivo: To circumvent the opacity of living tissues, investigators have observed angiogenesis through “windows” in living animals that include the naturally transparent tails of amphibian larvae (Clark and Clark 1939), or specialized viewing chambers either implanted into rabbit ears (Clark and Clark 1939), mouse skin (Algire, Chalkley et al. 1945) and hamster cheek pouches (Greenblatt and Shubi 1968) or developed from rabbit corneal pockets (Gimbrone, Cotran et al. 1974) or chick chorioallantoic membranes (Ausprunk, Knighton et al. 1974). From these early, largely descriptive studies came validation of the central paradigm of tumor-induced vascular chemotaxis and the corresponding discovery of diffusible tumor-derived molecules that promote vascular growth. Newer assays of angiogenesis in vivo measure vascular ingrowth into polymeric sponges or plugs of gelled basement membrane proteins implanted subcutaneously into rodents (Passaniti, Taylor et al. 1992; Andrade, Macahado et al. 1997; Akhtar, Dickerson et al. 2002; Koike, Vernon et al. 2003). For all of their elegance, approaches in vivo are made difficult by: (1) intra-species variation in angiogenic response from animal to animal; (2) the lack of translation of results from one species to another, (3) high costs of animal purchase and maintenance; (4) public disapproval of the use of animals for research purposes; (5) complexities encountered in animal surgeries and in the visualization and evaluation of results. Two-dimensional (2D) models of angiogenesis in vitro; In an effort to understand the molecular mechanics of angiogenesis, endothelial cells isolated from large vessels were cultured in flat dishes until they formed confluent, pavement-like monolayers that simulated the endothelial linings of blood vessels (Jaffe, Nachman et al. 1973; Gimbrone 1976). Although useful as models of proliferative responses to endothelial injury in large blood vessels (Gimbrone, Cotran et al. 1974: Fishman, Ryan et al. 1975; Madri and Stenn 1982; Madri and Pratt 1986; Jozaki, Marucha et al. 1990; Rosen, Meromsky et al. 1990), monolayer cultures of endothelial cells on rigid substrata do not typically organize into capillary-like tubes in simulation of angiogenesis. In 1980, however, following successful long-term culture of capillary endothelial cells (Folkman, Haudenschild et al. 1979), it was reported that 20-40 day cultures of bovine or human capillary endothelial cells developed a 2D cellular network on top of the confluent cellular monolayer, a process termed “angiogenesis in vitro” (Folkman and Haudenschild 1980). The endothelial cells of the network appeared as “tubes” with “lumens” filled with a fibrillar/amorphous material that was interpreted to be an endogenously-synthesized network of “mandrels” on which the cells organized. Later studies reported similar 2D network formation by endothelial cells from large vessels (Maciag, Kadish et al. 1982; Madri 1982; Feder, Marasa et al. 1983) and by endothelial cells seeded on top of malleable, hydrated gels of basement membrane proteins (e.g. Matrigel® gel) (Kubota, Kleinman et al. 1988).

Although 2D models of vascular development remain in use today (the Matrigel®-based assay (Kubota, Kleinman et al. 1988) is available commercially), such models lack the following 5 defining characteristics of true angiogenesis:

-   1. Invasion—Endothelial cells in 2D models form networks on top of     extracellular matrix and show little propensity to burrow into the     extracellular matrix (Vernon, Angello et al. 1992; Vernon, Lara et     al. 1995). -   2. Directionality—In 2D models, the networks of endothelial cells     form in vitro more or less simultaneously throughout a field of     pre-positioned cells, whereas angiogenesis in vivo involves the     vectorial invasion of extracellular matrix by filamentous sprouts     that arborize by multiple levels of branching. -   3. Correct polarity—Although the 2D models make unicellular tubes     that markedly resemble capillaries (Maciag, Kadish et al. 1982;     Feder, Marasa et al. 1983; Sage and Vernon 1994) their polarity is     “inside-out”, that is, they deposit basement membrane material on     their luminal surfaces and have their thrombogenic surfaces facing     outward to the surrounding culture media (Maciag, Kadish et al.     1982; Feder, Marasa et al. 1983)—opposite to the situation in vivo. -   4. Lumen formation—Evidence that 2D models generate endothelial cell     (EC) tubes with patent lumens is weak. Typically, the endothelial     cell tubes have “luminal” spaces that are filled with extracellular     matrix (either exogenous or synthesized by the cells) (Maciag,     Kadish et al. 1982; Madri 1982; Feder, Marasa et al. 1983; Sage and     Vernon 1994; Vernon, Lara et al. 1995). Where present, patent lumens     usually appear as slit-like or narrow cylindrical spaces bounded by     thick walls of endothelial cell cytoplasm quite different from the     inflated, thin-walled endothelial cell tubes that typify capillaries     in vivo. -   5. Cell specificity—The cellular networks in 2D models are generated     by mechanical processes that may be accomplished by non-EC cell     types (Vernon, Angello et al. 1992; Vernon, Lara et al. 1995).     Indeed, mathematical modeling has shown that any adherent cell type     capable of applying tensile forces to malleable, 2D extracellular     matrix (either synthesized endogenously or supplied (e.g., Matrigel®     gel)) can generate networks under optimal conditions (Manoussaki,     Lubkin et al. 1996).     Three-dimensional (3D) models of angiogenesis in vitro: The     recognition that angiogenesis in vivo occurs within a 3D     extracellular matrix has led to a variety of models in which     sprouting is induced within 3D gels of extracellular matrix in     vitro. In an early 3D model, endothelial cells dispersed within     collagen gels (Montesano, Orci et al. 1983) formed networks of cords     and tubes (Elsdale and Bard 1972). Although the endothelial cell     tubes exhibited correct polarity, the characteristics of invasion     and directionality were lacking (the endothelial cells were     pre-embedded and evenly dispersed in the extracellular matrix).     Nonetheless, this approach has proven useful in studies of lumen     formation (Davis and Camarillo 1996) and of responses of endothelial     cells to growth factors (Madri, Pratt et al. 1988; Merwin, Anderson     et al. 1990; Kuzuya and Kinsella 1994; Marx, Perlmutter et al. 1994;     Davis and Camarillo 1996).

In an alternative approach, 1 mm sections (rings) of rat aorta embedded in a 3D plasma clot generated branching, anastomosing tubes (Nicosia, Tchao et al. 1982). Sprouts from the aortic rings exhibited angiogenesis-like invasion and directionality in addition to polarity. Explant models utilizing aortic rings from rats or microvascular segments from mice have been used to study the influence of tumors, growth factors, various extracellular matrix supports, and conditions of aging on angiogenesis (Nicosia, Tchao et al. 1983; Mori. Sadahira et al. 1988; Nicosia and Ottinetti 1990; Nicosia, Bonanno et al. 1992; Villaschi and Nicosia 1993; Nicosia, Bonanno et al. 1994; Nicosia, Nicosia et al. 1994; Nicosia and Tuszynski 1994; Hoying, Boswell et al. 1996; Arthur, Vernon et al. 1998).

A variety of models exist that induce purified endothelial cells (as monolayers or aggregates) to sprout invasively into underlying or surrounding 3D extracellular matrix gels (Montesano and Orci 1985; Pepper, Montesano et al. 1991; Montesano, Pepper et al. 1993; Nehls and Drenckhahn 1995; Nehls and Herrmann 1996; Vernon and Sage 1999; Vernon and Gooden 2002). Each of these models has specific limitations that include difficulty in visualizing sprout formation, limited sprouting, a requirement for sectioning, or lack of effectiveness with certain types of endothelial cells.

Wolverine and Gulec have disclosed a 3D angiogenesis system (US 2002/0150879 A1) that involves embedding a fragment of tumor tissue into a matrix. The outgrowth of microvessels can be characterized to assay the angiogenic potential of the tissue. However, this approach does not provide luminal per-fusion of the microvessels.

Neumann (the inventor here) et al. 2003, has disclosed the possibility of creating perfused microvessels in vitro that can be included in an artificial tissue. Neumann et al. 2003 teaches using 127 micrometer nylon fishing line as mandrels held by shrink tubing for making microvessels. The vessels were made from rat aortic smooth muscle cells embedded in agar. These microvessels were of an exploratory nature and not suitable for creating a human vessel graft.

Two-dimensional models of vascular growth in vitro do not establish the defining characteristics of angiogenesis listed previously, whereas existing 3D models reproduce some or most of the characteristics. Importantly, none of the 3D models currently available reconstruct a parent blood vessel that contains a pressurized, flowing, circulatory fluid. Consequently, none of the existing in vitro 3D models permit study of the contribution of luminal pressure and flow to vascular growth and morphogenesis.

SUMMARY OF THE DISCLOSURE

A method for creating networks of perfusable microvessels in vitro, is disclosed. A mandrel is drawn through a matrix to form a channel through the matrix. Cells are injected into the channel, the channel having an inner wall. The matrix is incubated to allow the cells to attach to the inner wall. The channel is perfused to remove unattached cells to create a parent vessel, where the parent vessel includes a perfusable hollow channel lined with cells in the matrix. The parent vessel is induced to create sprouts into the surrounding matrix get so as to form a microvessel network. The microvessel network is subjected to luminal perfusion through the parent vessel.

The present disclosure provides methods and systems that overcome the limitations of existing models of angiogenesis by combining proven methods for generating invasive, tubular, microvascular sprouts in 3D extracellular matrix (ECM) with novel methodologies for the fabrication of a tissue-engineered parent vessel that will be the source of luminal flow. Via the perfusate, angiogenesis-modulatory compounds can be administered to the luminal surface of endothelial cells where specific target receptors are known to reside. The presence of a luminal flow of nutrient medium will substantially increase the survival time of capillary tubes in vitro. The disclosed angiogenesis system can be used evaluate a variety of experimental parameters that include hypoxia/hyperoxia, test of specific soluble bioactive compounds, use of genetically modified cells, and gene delivery via viral transfection. The system allows the study of angiogenesis relative to wound repair, aging, cancer and atherosclerosis. Importantly, a model following the teachings of the present invention may be adapted to provide fully functional vascular systems capable of being incorporated into bioengineered artificial tissues.

The present disclosure also provides new and novel approaches, including a manifold design for making microvessels, making microvessels from endothelial cells and making larger vessels (e.g. having the size of coronary arteries). These and other important new teachings, including, for example, a method for creation of microvascular networks are evident from the specification and claims hereinbelow.

BRIEF DESCRIPTION OF THE DRAWINGS

FIG. 1A, FIG. 1B and FIG. 1C schematically show an example of parent-vessel creation.

FIG. 2A, FIG. 2B, FIG. 2C and FIG. 2D schematically show an example of a known heat-shrink process.

FIG. 3A schematically shows a known design for mounting culture/perfusion devices.

FIG. 3B schematically shows a design used in a manufacturing method for mounting culture/perfusion devices.

FIG. 4A and FIG. 4B schematically show creation of manifolds for culture/perfusion devices.

FIG. 5A, FIG. 5B and FIG. 5C schematically show an alternative design for microfabricated culture/perfusion devices.

FIG. 6 schematically shows a cell-seeding procedure.

FIG. 7 shows a schematic of a capillary network between two bioartificial parent vessels.

FIG. 8 a shows an in vitro image of an example of a plurality of mandrels after seeding with smooth muscle cells.

FIG. 8 b shows an example of a perfused muscle plate.

FIG. 9 schematically shows an alternate embodiment of a CPD.

FIG. 10 shows a single parent vessel growing sprouts into the surrounding matrix.

FIG. 11 shows one parent vessel connected through a network of sprouts to a second parent vessel.

FIG. 12, an alternate method for creating parent cells by seeding cells into channels in a collagen matrix is shown

DETAILED DESCRIPTION OF THE PREFERRED EMBODIMENTS

The examples presented herein are for the purpose of furthering an understanding of the invention. The examples are illustrative and the invention is not limited to the example embodiments. The method of the present invention is useful for the study of physiological and pathological vascular growth, and vascular growth in response to angiogenic or angiostatic factors. Other useful applications are to methods that evaluate the angiogenic potential of cancer tissues and the response to antiangiogenic drugs. Additionally, the method of the invention may be used to construct various wound-healing devices and for vascularization of tissue-engineered constructs.

In one example a method and device for the creation of perfusable three-dimensional microvessel networks is disclosed. As used herein “EC” refers to endothelial cells, “SMC” refers to smooth muscle cells and “CAS” refers to coronary-artery substitutes.

Generally, the devices for the culture and perfusion of microvessel networks consist of a chamber holding one or more mandrels in the center (as best shown in FIG. 1). The chambers can be fabricated from any biocompatible material and by a number of techniques, for example, by sandwiching laser-cut frames. The mandrels are assembled within the chamber in such way that they are retractable. This can be achieved by fitting the ends of the mandrels into tubing, as for example, by heat shrinking, (as demonstrated in FIG. 2). The diameter of the mandrels depends on the desired vessel caliber. The setup can be modified to accommodate single vessels, two vessels, or up entire arrays of vessels in 2D or 3D. Mandrels can be of various materials, such as polymer fibers, glass fibers, wires or the like.

Microvessels are created by seeding cells onto the mandrels, stimulating the cells to multiply around the mandrels, and extracting the mandrels when cells have formed vessel walls. The vessels are then embedded in a matrix. Depending on the culture conditions, the composition of the matrix, and the presence of angiogenic stimuli (e.g. growth factors), the parent vessels will sprout into the surrounding matrix. The sprouts will anastomoze with each other and, thus leading to the formation of capillary networks. After removal of the mandrels, the devices are connected to a perfusion system, and vessels are subjected to luminal fluid flow.

Referring now to FIG. 1A, FIG. 1B and FIG. 1C, there shown is an example schematic of parent-vessel creation. FIG. 1A shows endothelial cells 1 in a culture growth medium 100, seeded onto mandrel 2 held by shrink tubing 4 in a device body 3. FIG. 1B shows that the cells 1 have multiplied and formed a circular layer in the form of cell-sleeve 102. FIG. 1 c shows the cell-sleeve after extraction of the mandrel 2 in an extracellular matrix (ECM) gel 110 being perfused with culture growth medium 100.

The method disclosed herein comprises the engineering of perfusable bioartificial vessel structures for tissue-engineering applications and research models. The general principle of the disclosed method involves the culture of cells in layers around removable mandrels that are tightly fit into thin-wall tubing or other fittings. Once the cell layers have reached a desired wall thickness, the mandrels are removed, and the hereby-created bioartificial vessels (BAVs) may be perfused with culture medium, blood, blood substitutes, or other fluids by aid of a perfusion system. The disclosed method allows for the production of mass manufactured or custom-created blood vessels, perfused in vitro angiogenesis models, wound healing devices, tissue components, whole tissues and organs, as well as research models.

Manufacture of Culture/Perfusion Devices

Referring now to FIG. 2A, FIG. 2B, FIG. 2C and FIG. 2D there shown is an example schematic of a known heat-shrink process. As shown specifically in FIG. 2A each culture/perfusion device (CPD) may comprise one or more mandrels 2 held by a supporting frame 12. The mandrels 2 of the diameter of the desired vessel caliber are fit with their ends tightly into medical-grade shrink tubing segments 4. The mandrels 2 may comprise biocompatible fibers (e.g. polymer, glass, wires or equivalents) having diameters from several micrometers up to several millimeters depending on the vessel size being emulated. In one example, microcapillary tubing comprising optical fibers was employed as mandrels.

As shown in the more detailed drawing of FIG. 2B, a central portion 14 of each shrink tubing segment 4 is heat-shrunk around one of the mandrels 2. Subsequently, as specifically shown in FIG. 2C, the mandrel 2 is retracted, and the tubing cut. FIG. 2D shows the situation after re-positioning the mandrel such that both ends of the mandrel are enclosed by the now cut-and-separated shrink tubing segment 4. The frames 12 may be fabricated using various materials and techniques. The setup may be modified to accommodate either single bioartificial vessels or arrays of bioartificial vessels. Similarly, by layering several planes of mandrel arrays, a thick, perfusable tissue may be generated with vascular networks.

Machining of Perfusion Chambers

Referring now to FIG. 3A a known setup for the perfusion of several mandrel/shrink-tubing assemblies 11 is shown. A frame 20 may advantageously be milled from polycarbonate or equivalent materials. Distribution chambers 30 may be included into the design, which allows for simultaneous perfusion of many bioartificial vessels. Ends of a set of threads comprising the mandrels 2 are gathered in a silicon tube 23.

Laser Cutting of Mylar Frames

Referring now to FIG. 3B a novel design used in a manufacturing method for mounting culture/perfusion devices is schematically shown. A single vessel design, CPD 70, may advantageously be created by sandwiching a mandrel 2 held by heat-shrink tubing 4 between two laser-cut Mylar® frames 22. A cylindrical epoxy manifold 21, constructed as detailed below, may advantageously be used for holding the mandrel/shrink-tubing assembly 11.

Mandrel/shrink-tubing assemblies may be sandwiched between two frames of a polyester film or the like, such as Mylar®, with adhesive sides pressed together such that each mandrel is suspended in the frame window 76 by two shrink-tubing segments 4′ at each end. The two shrink-tubing segments 4′ are stabilized and strengthened by inclusion of at least one thin stabilizing wire 26 in the frame 22 and by encapsulation in cylindrical epoxy manifolds that are cast around the shrink-tubing and the at least one thin stabilizing wire 26 by use of a mold of silicone tubing. The two shrink-tubing segments 4′ will eventually become the inflow and outflow ports for the CPD 70.

Referring now to FIG. 4A and FIG. 4B, there schematically shown is a method for creation of manifolds for culture profusion devices. FIG. 4A particularly shows a plurality of shrink-tubing/mandrel assemblies 11 pulled through a sleeve of for example, silicone tubing 50. An epoxy glue 40 is injected to fill the silicone tubing 50 and allowed to harden.

FIG. 4B particularly shows the condition after the epoxy glue 40 has hardened and the silicone tubing 50 is slit open and removed. Remaining is a hardened epoxy rod 44. The epoxy rod 44 is cut after the mandrels have been retracted behind the cutting spot leaving channels 42 created by the shrink tubing. The ends 46 of many shrink tubes may be integrated to form a manifold 21. Stacking of individual CPDs or CPD frame assemblies can be used to create 3D vessel arrays.

Alternative Methods

Referring now to FIG. 5A FIG. 5B and FIG. 5C there schematically shown is an alternative design for microfabricated culture/perfusion devices. FIG. 5A particularly shows a set of mandrels 2 introduced through small perforations 54 in a frame where the perforations have sleeves 56, which substitute for the shrink tubing. FIG. 5B particularly shows a CPD before cell seeding including a set of mandrels 2 mounted in a frame wall 52.

FIG. 5C particularly shows an alternate example of a culture/perfusion device with vessels 62 where microfabricated manifolds 64 may be attached to the sleeves 56 on the outside of the frame 52. The vessels 62 are grown on mandrels as shown herein and remain after the mandrels are removed. Microfabrication methods, such as micro molding, may be used for the mass production of such CPD frame assemblies.

Vessel Creation and Perfusion

Referring now to FIG. 6 there schematically shown is a cell-seeding procedure. In order to prepare the CPDs 70 for cell seeding, they are first cleaned and then UV-sterilized. Under sterile conditions, the CPDs are fixed to a surface, e.g. the bottom of the Petri dish 72. The inner window 76 (as shown in FIG. 3B) of the CPD frame assembly 70 is then filled with a solution that contains an attachment-protein, such as laminin-1. One or more spacers 77 may be used as necessary. After an incubation period, the attachment-protein containing solution is removed, and a suspension of the desired cell type (e.g. smooth muscle cells or endothelia cells) in culture medium is then transferred into the window 76 of the CPD 70.

Cell seeding may be done by filling a volume of cell suspension into the window, and flipping the CPD frame assembly 70 upside down, thus creating a hanging droplet 80. During an incubation period of about 45 min., a large number of cells will attach to the mandrel/shrink tubing assemblies within the CPD frame assembly. Excessive cells will sink into the tip of the hanging drop and may be easily collected and discarded. The Petri dish, containing one or more CPD frame assemblies, is then returned into an upright position, filled with culture medium until the CPD frame assemblies are flooded, and incubated. The incubation conditions in one example were in an environment of 5% CO₂ at 37° C., The cells attached to the mandrel/shrink tubing assemblies will spread out and multiply, forming concentric monolayers (e.g. endothelial cells) or multilayer of 150 μm and more in thickness (e.g. smooth muscle cells).

At the desired wall configuration or thickness the mandrels are extracted, thereby creating hollow cellular tubes. Thinner walls may be protected from rupture by casting a gel such as, for example, agarose, collagen, a gel of basement membrane proteins or the like, around the cell sleeves prior to mandrel extraction. The manifolds of the CPD frame assemblies are then connected to a perfusion system and perfused with the fluid of choice, such as growth medium.

In another embodiment, a method for the creation of endothelial “parent” vessels from human vascular endothelial cells (HUVEC) comprises the steps wherein:

-   -   The culture device is first cleaned and then sterilized by UV         exposure for 30 min. from each side. Under sterile conditions,         the device is fixed to the bottom of a Petri dish with sterile         strips.     -   The inner window of the device is then filled with an         attachment-protein solution of laminin-1 (other attachments         proteins, such as fibronectin, fibrin, or gelatin can be used         instead).     -   After overnight incubation, the attachment-protein containing         solution is removed, and a suspension of human vascular         endothelial cells in culture medium is then transferred into the         window of the device.     -   The Petri dish is then flipped upside down, thus creating a         hanging drop of cell-medium suspension in the window of the         device. After a 45 min. incubation period in a cell culture         incubator (5% CO₂, 37° C.) a large number of cells will be         attached to the mandrel/shrink tubing assemblies within the         devices.     -   The Petri dish is then brought back into the upright position,         and filled with growth medium for human vascular endothelial         cells until the device is submerged.     -   Cells not bound to the mandrels will float off and can be         aspirated and discarded.     -   The Petri dish is then placed in an incubator (5% CO₂, 37° C.).         The cells attached to the mandrels will spread out and multiply,         forming concentric monolayers of human vascular endothelial         cells.     -   The culture medium is then removed from the Petri dish. A         collagen solution is filled into the window of the culture         device, and allowed to solidify, thus embedding the mandrel with         the cell layer.     -   The human vascular endothelial cells will form sprouts into the         collagen gel. The mandrel is then slowly extracted, leaving         behind a perfusable “parent” microvessel of human vascular         endothelial cells.     -   The manifolds of the device are then connected to a perfusion         system and perfused with human vascular endothelial cells growth         medium.

Perfusion System

The CPDs may be attached to perfusion systems either in linear or in circulatory mode. A linear setup may be created with a gravity flow system, or a commercially available or custom-built syringe pump. Syringes are filled with perfusion medium, mounted into the syringe pump and connected to the upstream ends of the CPDs via gas-tight tubing. The CPDs may be stored in an incubator under sterile conditions or a sterile cell culture environment may be established within the CPU. The downstream manifold of the CPDs are connected to end reservoirs that collect the perfusate. A circulatory system may be built by using a peristaltic pump. Both, the linear and the circulatory system may be fitted with devices for gas exchange. Gas concentration, perfusion pressure flow, temperature, and the concentration of nutrients and metabolic byproducts are measured with sensors. The collected data may be fed into a feedback loop, allowing for tight control of the desired parameters.

Specific Applications Models for Angiogenesis Related Research

Referring now to FIG. 7, FIG. 7 shows a schematic of a capillary network between two bioartificial parent vessels 200, 202. The fluid perfusate 204 is re-routed through the capillaries 206 by decreasing the flow (f) into the “venous” parent vessel 202, and increasing the resistance (R) in the “arterial” parent vessel 200. Consequently, the perfusate 204 is driven from the vessel with higher pressure to the vessel with lower pressure, simulating natural blood flow from the arterial end to the venous end of the capillary bed.

The mandrel method may be also used for the development of models for angiogenesis research, as needed for pharmaceutical testing and research in wound repair, aging, and diseases like cancer, diabetes, arthritis, and psoriasis. Using endothelial cells only, or combinations of endothelial cells, smooth muscle cells, and pericytes, parent bioartificial microvessels (BMVs) can be cultured around micron-diameter mandrels, and embedded into a supportive gel of extracellular matrix. The mandrels will then be extracted, leaving behind patent endothelial cell tubes within the extracellular matrix gel 210. The extraction may be done by hand, or by aid of an automated device, and with speeds varying from extremely slow to extremely fast. Other variations may include the extraction of the mandrel from bioartificial microvessels in a frozen state, coating of the mandrels with a thermo-responsive polymer, or pulling on either end of the mandrel, and thereby thinning it until rupture.

The sprouting of the parent vessels into the surrounding gel 210 will be induced by compounds, such as basic fibroblast growth factor (bFGF), vascular endothelial growth factor (VEGF), and phorbol 12-myristate-13-acetate (PMA), which are added to the gel and/or perfusate (e.g. growth medium).

Complex capillary networks 222 may be created by establishing a pressure difference between two adjacent parent bioartificial microvessels, thereby imitating arterial and venous blood flow. The fluid flow will then be re-directed from the “arterial” bioartificial microvessel through the interconnected sprouts into the “venous” bioartificial microvessel.

The perfusate may advantageously comprise oxygenated cell growth medium, free of serum and angiogenic or angiostatic substances. In another example the perfusate may be an oxygenated cell growth medium, supplemented with serum, and/or angiogenesis influencing compounds. In yet another example embodiment the perfusate may be an oxygenated physiological salt solution. In another example the perfusate may include oxygenated blood, blood components, or blood substitutes. In yet another example embodiment the perfusate may not be an oxygenated, and oxygenation of the system is achieved by diffusion through the matrix. In yet another example embodiment, angiogenic or angiostatic compounds may be added to a perfusate.

In one example embodiment, angiogenic and angiostatic compounds or the like are added to the matrix. In yet another example embodiment cells comprise genetically modified cells that release products into a perfusate or into the matrix. In yet another example embodiment the matrix may advantageously comprise fibrin, collagen, basement-membrane matrices and gelatin. One type of useful matrix is Matrigel® gel. In another example embodiment the matrix may comprise agar, agarose, alginate, or silica gel.

In one example embodiment, the cells may be selected from the group consisting of endothelial cells, smooth muscle cells, pericytes, human cells, animal cells, plant cells, stem cells, muscle cells, liver cells, kidney cells, lung cells, skin cells, epithelial cells and genetically modified cells. Similarly, the matrix may be populated with cells selected from the group consisting of endothelial cells, smooth muscle cells, pericytes, human cells, animal cells, plant cells, stem cells, muscle cells, liver cells, kidney cells, lung cells, skin cells, epithelial cells and genetically modified cells, either dispersed throughout the matrix, or locally concentrated. In some cases a fragment of healthy or diseased tissue, such as cancer tissue is embedded into the matrix.

Sprouting from parent vessels may be microscopically studied in vitro, in sectioned material or in whole-mount preparations. Perfusion of the bioartificial microvessels with fluorescent solutions (e.g. fluorescent dextrans) aids analysis of the sprout diameter, the patency of sprout lumens, and the degree of anastomization. 3D reconstruction of sprout morphologies may be performed by z-axis stacking of epifluorescence images taken by a confocal microscope. The synthesis of a pericellular basement-membrane matrix by sprouts 220 may be monitored in whole mounts and in histological (paraffin) sections by immunolabeling with anti-laminin and type IV collagen primary antibodies and fluorescent or peroxidase-tagged second antibodies.

In composite EC/SMC sprouts, the spatial relationships between the two cell types may be examined by labeling endothelial cells with a FITC-monoclonal antibody (MAb) to human CD31 (clone P2B1—Chemicon) or FITC-UEA 1 agglutinin—a specific marker for human endothelial cells. smooth muscle cells may be labeled with a MAb to human alpha-SM actin followed by RITC-anti-mouse second antibodies. Details of luminal structure and interaction between endothelial cells and smooth muscle cells may be obtained from paraffin sections labeled with the aforementioned reagents.

The described fabrication methods are the foundation for commercial mass-production of angiogenesis devices with a high repeatability. With suitable preservation (e.g. cryostorage), pre-grown parent vessels or whole capillary networks could be made available to researchers in off-the-shelf fashion.

Coronary-Artery Substitutes

For the creation of coronary-artery substitutes, mandrels with an outer diameter selected to yield a coronary artery substitute having a vessel lumen with an inner diameter of approximately 4 mm to 5.5 mm. Alternatively, the mandrel may be a hollow tube that is perfused and permeable enough to allow for exchange of nutrients and gases during the growth period of the coronary-artery substitute. The coronary-artery substitutes may be grown either solely from smooth muscle cells, thus presenting a structure analog to the media layer in blood vessels, or made as composite structures from two or three cell types.

Smooth muscle cells are seeded onto the mandrels and grown to circular layers of 300-400 μm. In order to speed up the creation of coronary-artery substitutes, the SMC-phenotype may be manipulated in such way that the cells are brought into a highly proliferative phenotype during the initial growth phase, and then switched to a differentiated state after the vessel wall has reached the desired thickness. The phenotype switch will cause the smooth muscle cell's to dramatically slow down their growth rate, and induce the production of extracellular matrix proteins, such as collagen and elastin, which affect mechanical properties of the vessels. The phenotype switch may be achieved by controlling the expression of certain genes. For example, with aid of a tetracycline-responsive promoter, gene expression (e.g. for elastin) may be suppressed until the vessel wall has reached the desired thickness. Omitting tetracycline from the growth medium will then activate the inserted gene. Over-expression of elastin, for instance, will inhibit further cell proliferation and exert structural and signaling functions within the vessel wall. Mechanical conditioning, e.g. pulsatile flow may be used to strengthen the coronary-artery substitutes, and induce physiological alignment of the cells. Other external or internal “phenotype switches” may be potentially used, as well.

Endothelial cells may be seeded into the SMC sleeves either directly after removal of the mandrel, or after the conditioning and restructuring of the smooth muscle cells. Endothelial cell seeding may be done by infusion of an endothelial cell suspension into the SMC sleeve. The flow is then stopped for a period of time to allow proper attachment of the endothelial cells. If necessary, the vessels may be rotated, or repeatedly flipped upside down in order to facilitate an even distribution of the endothelial cells.

Alternatively, endothelial cells may be seeded onto the mandrel first. In that case smooth muscle cells are seeded onto a confluent endothelial cell layer. For this method, it will be necessary to prevent the endothelial cells from migration towards the periphery of the coronary-artery substitute, which is richer in oxygen and nutrients.

If desired, seedling fibroblast cells onto the outside of the SMC sleeves can create an adventitial layer.

The cells for creating coronary-artery substitutes may be derived from autologous, heterologous, or xenogeneic material. The cells may be stem cells, precursor cells, or differentiated cells. The cells may be genetically modified to achieve a specific phenotype or to lower the immune response of the host organism.

The herein-disclosed CPD method provides the option for mass-producing off-the-shelf vessel substitutes, or vessel substitutes that are custom designed for the recipient. The herein-disclosed CPD method is also suitable for the development of models for tissue engineering of coronary-artery substitutes, for research in atherogenesis, arteriogenesis, for research in the interaction of different vascular cell types with each other and with extracellular matrix components, for studies on the effects of nitric oxide, and for the study of varies pharmaceuticals.

Blood and Lymphatic Vessels of Different Size or Type

The herein-disclosed CPD method may be used to create blood vessels in diameter and type other than coronary arteries. Changing the diameter of the mandrel will vary the vessel diameter. The type of the vessel (arterial, venous lymphatic) may be varied with the phenotype of the cells and/or the time point when the proliferation of the cells is inhibited. Veins, for example, contain only a small smooth muscle cell layer.

Other Tubular-Like Tissues

The herein-disclosed CPD method may be used for the engineering of other tubular tissues, such as bile duct, lacrimal duct, pharyngotympany tube, oviduct, vas deferens, ureter, urethra, pulmonary airways etc. The herein-disclosed CPD method may also prove useful for the generation of nerve conduits from different cell types, including glial cells, for guidance of neural growth and repair.

BAV Systems for Engineered Tissues

The herein-disclosed CPD method may be used for the engineering of tissues and organs by using arrays of removable mandrels as scaffold. The cells of the desired tissue/organ (muscle, liver, kidney, lung, skin, etc.) are seeded onto the attachment-protein coated mandrels. These mandrels may be made from solid fibers or wires, or, alternatively from perfusable permeable tubes, such cellulose. The mandrels are separated from each other in a precise spacing that allows the single cell sleeves to merge. With this method, sheets or blocks of tissue may be formed. The mandrels are then extracted (or differently removed), and the bioartificial tissue is internally perfused by aid of a perfusion system.

Wound Healing Device

Pre-manufactured bioartificial vessel systems may be used to assist in wound healing, such as for chronic ulcers in diabetic patients. Bioartificial capillary networks could be embedded into patches of supportive materials (e.g. from extracellular matrix gels, enriched with angiogenic growth factors), and placed onto the wound. Autonomously perfused with oxygenized nutrient solutions, the bioartificial vessel would facilitate the sprouting of the donor vasculature and skin. Alternatively, such a bioartificial vessel patch could be sandwiched between the wound and a skin graft, and facilitate the in-growth of the graft.

Gene-Therapy Device

Bioartificial vessels could be used for implantable drug delivery devices. Cells, taken from a patient, could be genetically modified in vitro to produce a certain protein (hormone, enzyme etc.). These cells may be then grown into bioartificial vessels or vascular networks, using the aforementioned method. Re-implanted into the host, the cells continue to produce the target substance and release it locally or systemically.

Artificial Tissues and Organs

Tissue engineered vascular networks, as described above, may be used for the creation of tissues, or even whole organs. One approach is the creation of one or more in vitro perfused parent vessels. Stroma cells from the desired tissue or organ are seeded around the parent vessels, as for example, in a gel. The stroma cells are supplied with nutrients and oxygen via the parent vessels. When the stroma cells multiply, the demand for nutrients and oxygen increases. The cells release angiogenic factors, and stimulate the vessels to sprout. The vessel system sprouts in the same rate, as the tissue grows—very similar to the natural growth. Therefore, this system would be also a good model for studies in developmental biology.

Another approach utilizes parallel arrays of mandrels as a scaffold for stroma cells. As the stroma cells multiply, cell layers are formed around the mandrels. Eventually the space between all the mandrels is filled with stroma cells, resulting in a sheet of tissue. Upon removal of the mandrels, the tissue may be perfused through the channels, left behind by the mandrels. Those channels can become endothelialized through luminal seeding. The approach is not limited to 2D. Either several sheets may be stacked, or 3D scaffolds may be used. The inventor herein has used 2D arrays as well as 3D arrays for the engineering of muscle tissue.

In yet another approach, layers of tissue and layers of vascular networks could be created independently, and then intermittently stacked. All these approaches can produce either simple models with one or two cell types, or rather complex constructs composed of several cell types.

Upon implantation, the tissues or organs, engineered with these methods could be either connected directly to the blood stream, or kept perfused by a perfusion system until the host vasculature has grown into the graft.

Example of Perfused Tissue Engineered Muscle Construct

Referring now to FIG. 8 a, an in vitro image of an example of a plurality of mandrels after seeding with smooth muscle cells is shown. A plurality of mandrel-and-shrink tubing units M were sandwiched on a Mylar® frame. The distance between the mandrels M was adjusted to approximately 100 μm. The ends of all shrink tubing segments were combined in one upstream and one downstream manifold (not shown). The Mylar frame was sterilized, laminin coated and seeded with a suspension of 5×10⁶ rat aortic smooth muscle cells SM (RASMCs)/ml. The cells SM attached to each individual mandrel M and multiplied, thus forming circular layers. After 10 days, the individual layers had merged and resulted in one thick sheet or plate of smooth muscle cells. After additional 7 days in growth medium, the medium was supplemented with 50 U/ml heparin for another 7 days. Then, all mandrels were extracted, and the tissue perfused with heparin-medium at a rate of 10 ml/day. The perfusion chamber was kept fixed to the bottom of a 100-mm Petri dish filled with heparin-medium. The SMC plate was perfused for 11 days, Over that time, the channels CH remained functional and remained clearly visible in vitro (as best shown in FIG. 8 b).

Referring now to FIG. 8 b, an example of a perfused muscle plate MP is shown. Fluid is shown perfused through the tubing ends (T) into channels (CH) left behind by the extracted mandrels.

Referring now to FIG. 9, an alternate embodiment of a CPD is schematically shown. In one example, a CPD 900 includes a layer 902 juxtaposed between a first glass slide 904 and a second glass slide 920. The layer 902 has a thickness suitable for embedding a plurality of fluid ports connected by channels 922. The plurality of fluid ports include a cell suspension port 914, a plurality of inlet ports 912 and a plurality of outlet ports 918. Ports that are connected by channels 922 to allow for passage and sharing of fluids function similarly. Multiple ports, such as ports 912, are arranged to provide multiple access points. Other applications may advantageously employ microfluidic designs with fluid chambers and ports created in microfluidic materials. Similarly, the layer may comprise silicone or other materials suitable for use in microscopy or microfluidic applications. A collagen chamber 906 is advantageously located for access by a pair of hollow, flexible capillary tubes 916. The number of capillary tubes employed may range from one to substantially more than two as may be accommodated by the size of the CPD and the number of vessels being created. Each of the plurality of ports and chambers may be accessed through the layer by one or more syringe pumps through tubing inlets 940A, 940B, where the syringe pumps are attached to syringes having needles. While only two syringe pump tube inlets 940A, 940B are shown to simplify the drawings, it will be understood that separate syringe pumps, syringes or equivalents may be used for injecting or extracting materials into each chamber and/or port as the case may be. In one embodiment, the syringe pumps are coupled to gas tight syringes.

Having described the features of the alternate embodiment CPD 900, it will aid the understanding of the invention to now describe one method for constructing the CPD. In one example employing a silicone layer for layer 902, a pattern of holes and channels is punched into a silicone layer covered with an adhesive top layer 943 and adhesive bottom layer 945. Then, hollow needles are punctured through the silicone, which are then used to guide polyimide-coated fused-silica capillaries 916 into the collagen chamber 906 and also into one of the inlet ports 912. The two capillary tubes are held by small-bore tubing 910, leading from the main chamber into the outlet ports 908. The silicone layer 902 is then sandwiched in between two glass slides with aid of the adhesive layers. The CPD 900 is then autoclaved and stored until use. To get the chamber 906 ready for vessel creation, a collagen solution is prepared, injected through a syringe needle directly into the collagen chamber 906, and allowed to get in an incubator overnight. The CPD 900 is then connected to a syringe pump by injecting syringe needles into the two inlet ports.

The syringe needles are in turn, connected to gas-tight tubing, which leads to two gas-tight syringes, filled with grow medium with well adjusted pH, and mounted into a syringe pump. The two outlet ports 908A, 908B are connected to waste reservoirs in similar fashion. The syringe pumps, here operating as perfusion pumps, are then turned on, thereby filling the inlet ports and sequentially priming the inlet ports, the capillary tubes, and the outlet ports. When all the air is pushed out of the system, the each capillary tube is grabbed with tweezers and the ends that reach into the collagen chamber are pulled back through the collagen gel until only the ends of the capillaries reach into the matrix chamber. With this procedure, two perfusable channels are created in the collagen gel. In order to seed cells into the collagen channels, a highly concentrated suspension of endothelial cells is injected into the ports for cell suspension. The syringe pump is then turned off, and the other ends of the capillaries are then pulled back into the small reservoirs 914R that contain the cells, leading to an immediate influx of large numbers of cells into the collagen channels. The flow rate of the cells can be tightly controlled through the height of the waste reservoirs. The CPD is then placed in an incubator for 45 min. for allowing the cells to attach to the walls of the collagen channels. The CPD can be flipped over several times or otherwise manipulated to distribute the cells optimally. Finally, the capillary tubes are pulled out of the cell reservoirs into reservoirs that are part of the inlet port, and the syringe pump is turned on and set to the desired perfusion rate. Excessive cells are washed out. This seeding procedure leads to two parent vessels with homogeneous monolayers of cells after allowing time for growth, where the time required is shorter for more highly concentrated numbers of cells injected into the tubes. Note that the mandrel may be removed from the matrix by extraction and/or decomposition, depending on the type of mandrel used.

Referring now to FIG. 10, a single parent vessel 1050 growing sprouts 1052 into a surrounding matrix 1054 is shown. When Human Umbilical Cord Vein Cells (HUVECs) are seeded into the collagen channels, the so created parent vessels begin to sprout into the collagen. These sprouts elongate and begin to branch. These branches eventually anastomoze with branches from the opposite parent vessel and, thus, form vascular networks.

Referring now to FIG. 11, a first parent vessel 1102 is shown connected through a network of sprouts 1106 to a second parent vessel 1104. The sprouts 1106 have lumens and are perfused.

Protocol for Creation of Parent Vessels

Referring now to FIG. 12, an alternate method for creating parent cells by seeding channels in a collagen matrix is shown. Having described the alternate CPD using a silicone layer, a specific example of an application for creating a microvessel system will now be described to facilitate understanding of the disclosure by those skilled in the art.

The CPD is sterilized in an autoclave, and kept in a sterile environment until use. A collagen solution is prepared and kept on ice. The collagen is filled into a small syringe. The syringe is fitted with a 30 G syringe needle, and the collagen solution is injected into the collagen chamber through the syringe needle until the chamber is completely filled with collagen 1002. A second syringe needle is injected from the opposite side of the chamber as an air outlet.

The CPD is then connected to a syringe pump by injecting syringe needles into the two inlet ports 1004. The syringe needles are, in turn, connected to gas-tight tubing, which leads to two gas-tight syringes, filled with grow medium with well adjusted pH, and mounted into the syringe pump. The two outlet ports are connected to waste containers in similar fashion (i.e. syringe needles injected into the outlet ports, with tubing leading to the waste containers) 1006.

The CPD is perfused by operating the syringe pump as a perfusion pump, thereby filling the inlet ports and sequentially priming the inlet ports, the capillary tubes, and the outlet ports 1008. When all the air is pushed out of the system (e.g. through small diameter syringe needles serving as removable air outlets), then each capillary tube is grabbed with tweezers and the ends that reach into the collagen chamber are pulled back through the collagen gel until only the ends of the capillaries reach into the chamber. With this procedure two perfusable channels are created in the collagen gel 1010.

In order to seed cells into the collagen channels, a highly concentrated suspension of endothelial cells is injected into the ports for cell suspension 1012. The syringe pump is then turned off, and the other ends of the capillary tubes are then pulled back from the inlet ports into the small reservoirs that contain the cells, leading to an immediate influx of large numbers of cells through the capillary tubes into the collagen channels 1014. The flow rate of the cells can be tightly controlled through the backpressure (height of the waste reservoirs). The capillaries are then pulled back further into the reservoirs that are connected to the inlet ports.

The CPD is then placed in an incubator for 45 min for allowing the cells to attach to the walls of the collagen channels 1016. The CPD can be flipped over several times or otherwise manipulated to distribute the cells optimally.

Finally, the syringe pump is turned on and set to a desired perfusion rate 1020. Excessive cells are washed out. This seeding procedure leads to two parent vessels with homogeneous monolayers of cells 1022. One or more microvessel networks may be created by perfusing the parent vessels as described above.

Alternately the procedure for creating the parent vessels may also include embedding mandrels into the collagen matrix, extracting the mandrels, and infusing cells into the channels left behind by the mandrels as well as seeding cells onto mandrels as described above with reference to FIG. 1A-1C and others. The combination of the two methods allows layering of different cell types.

The invention has been described herein in considerable detail in order to comply with the Patent Statutes and to provide those skilled in the art with the information needed to apply the novel principles of the present invention, and to construct and use such exemplary and specialized components as are required. However, it is to be understood that the invention may be carried out by specifically different equipment, and devices and reconstruction algorithms, and that various modifications, both as to the equipment details and operating procedures, may be accomplished without departing from the true spirit and scope of the present invention.

The complete disclosures of all references cited in this specification are hereby incorporated by reference. In the event of an otherwise irreconcilable conflict, however, the present specification shall control.

REFERENCES

-   Akhtar N, Dickerson E B, Auerbach R. 2002. The sponge/Matrigel     angiogenesis assay, Angiogenesis 5:75-80. -   Algire G H, Chalkley H W. Legallais F Y, Park H D. 1945. Vascular     reactions of normal and malignant tissues in vivo. I. Vascular     reactions of mice to wounds and to normal and neoplastic     transplants. J Natl Cancer Inst 6:73-85. -   Andrade S P, Machado R D, Teixeira A S, Belo A V, Tarso A M, Beraldo     W T. 1997. Sponge-induced angiogenesis in mice and the     pharmacological reactivity of the neovasculature quantitated by a     fluorimetric method. Microvasc Res 54:253-261. -   Arthur W T, Vernon R B, Sage E H, Reed M J. 1998. Growth factors     reverse the impaired sprouting of microvessels from aged mice.     Microvasc Res 55:260-270. -   Ausprunk D H, Knighton D R, Folkman J. 1974. Differentiation of     vascular endothelium in the chick chorioallantois: a structural and     autoradiographic study. Dev Biol 38:237-248. -   Clark E R, Clark E L. 1939. Microscopic observations on the growth     of blood capillaries in the living mammal. Am J Anat 64:251-301. -   Davis G E, Camarillo C W. 1996. An alpha 2 beta 1 integrin-dependent     pinocytic mechanism involving intracellular vacuole formation and     coalescence regulates capillary lumen and tube formation in     three-dimensional collagen matrix. Exp Cell Res 224:39-51. -   Elsdale T, Bard J. 1972. Collagen substrata for studies on cell     behavior. J Cell Biol 54:626-637. -   Feder J, Marasa J C, Olander J V. 1983. The formation of     capillary-like tubes by calf aortic endothelial cells grown in     vitro. J Cell Physiol 116:1-6 -   Fisherman J A, Ryan G B, Karnovsky M J. 1975. Endothelial     regeneration in the rat carotid artery and the significance of     endothelial denudation in the pathogenesis of myointimal thickening.     Lab Invest 32:339-351. -   Folkman J, Haudenschild C. 1980. Angiogenesis in vitro. Nature     288:551-556. -   Folkman J, Haudenschild C C, Zetter B R. 1979. Long-term culture of     capillary endothelial cells. Proc Natl Acad Sci USA 76:5217-5221. -   Gimbrone M A, Jr. 1976. Culture of vascular endothelium. In: Prog     Hemost Thromb. p 1-28. -   Gimbrone M A, Jr., Cotran R S, Folkman J. 1974a. Human vascular     endothelial cells in culture. Growth and DNA synthesis. J Cell Biol     60:673-684. -   Gimbrone M A, Jr., Cotran R S, Leapman S B, Folkman J. 1974b. Tumor     growth and neovascularization: an experiment model using the rabbit     cornea. J Natl Cancer Inst 52: 413-427. -   Greenblatt M, Shubi P. 1968. Tumor angiogenesis: transfilter     diffusion studies in the hamster by the transparent chamber     technique. J Natl Cancer Inst 41:111-124. -   Hoying J B, Boswell C A, Williams S K. 1996. Angiogenic potential of     microvessel fragments established in three-dimensional collagen     gels. In Vitro Cell Dev Biol Anim 32:409-419. -   Jaffe E A, Nachman R L, Becker C G, Minick C R. 1973. Culture of     human endothelial cells derived from umbilical veins. Identification     by morphologic and immunologic criteria. J Clin Invest 52:2745-2756. -   Jozaki K, Marucha P T, Despins A W, Kreutzer D L. 1990. An in vitro     model of cell migration: evaluation of vascular endothelial cell     migration. Anal Biochem 190:39-47 -   Koike T, Vernon R B, Gooden M D, Sadoun E, Reed M J. 2003. Inhibited     angiogenesis in aging: a role for TIMP-2. J Gerontol A Biol Sci Med     Sci 58:B798-805. -   Kubota Y, Kleinman H K, Martin G R, Lawley T J. 1988. Role of     laminin and basement membrane in the morphological differentiation     of human endothelial cells into capillary-like structures. J Cell     Biol 107:1589-1598. -   Kuzuya M, Kinsella J L. 1994. Induction of endothelial cell     differentiation in vitro by fibroblast-derived soluable factors. Exp     Cell Res 215:310-318. -   Maciag T, Kadish J, Wilkins L, Stemerman M B, Weinstein R. 1982.     Organizational behavior of human umbilical vein endothelial cells. J     Cell Biol 94:511-520. -   Madri J A. 1982. Endothelial cell-matrix interactions in hemostasis.     Prog Hemost Thromb 6:1-24. -   Madri J A, Pratt B M. 1986. Endothelial cell-matrix interactions: in     vitro models of angiogenesis. J Histochem Cytochem 34:85-91 -   Madri J A, Pratt B M, Tucker A M. 1988. Phenotypic modulation of     endothelial cells by transforming growth factor-beta depends upon     the composition and organization of the extracellular matrix. J Cell     Biol 106:1375-1384. -   Madri J A, Stenn K S. 1982. Aortic endothelial cell migration. I.     Matrix requirements and composition. Am J Pathol 106:180-186. -   Manoussaki D, Lubkin S R, Vernon R B, Murray J D. 1996. A mechanical     model for the formation of vascular networks in vitro. Acta Biotheor     44:271-282. -   Marx M, Perlmutter R A, Madri J A. 1994. Modulation of     platelet-derived growth factor receptor expression in microvascular     endothelial cells during in vitro angiogenesis. J Clin Invest     93:131-139. -   Merwin J R, Anderson J M, Kocher O, Van Itallie C M, Madri     J A. 1990. Transforming growth factor beta 1 modulates extracellular     matrix organization and cell-cell junctional complex formation     during in vitro angiogenesis, J Cell Physiol 142:117-128. -   Montesano R, Orci L. 1985. Tumor-promoting phorbol esters induce     angiogenesis in vitro. Cell 42:469-477. -   Montesano R, Orci L, Vassalli P. 1983. In vitro rapid organization     of endothelial cells into capillary-like networks is promoted by     collagen matrices. J Cell Biol 97:1648-1652. -   Montesano R, Pepper M S, Orci L. 1993. Paracrine induction of     angiogenesis in vitro by Swiss 3T3 fibroblasts. J Cell Sci 105 (Pt     4): 1013-1024. -   Mori M, Sadahira Y, Kawasaki S, Hayashi T, Notohara K, Awai M. 1988.     Capillary growth from reversed rat aortic segments cultured in     collagen gel, Acta Pathol Jpn 38:1503-1512. -   Nehls V. Drenckhahn D. 1995. A novel, microcarrier-based in vitro     assay for rapid and reliable quantification of three-dimensional     cell migration and angiogensis. Microvasc Res 50:311-322. -   Nehls V, Herrmann R. 1996. The configuration of fibrin clots     determines capillary morphogenesis and endothelial cell migration.     Microvasc Res 51:347-364. -   Neumann T, Nicholson B S, Sanders J E. 2003. Tissue engineering of     perfused microvessels, Microvasc Res 66:59-67. -   Nicosia R F, Bonanno E, Smith M, Yurchenco P. 1994a. Modulation of     angiogenesis in vitro by laminin-entactin complex. Dev Biol     164:197-206. -   Nicosia R F, Bonanno E. Villaschi S. 1992. Large-vessel endothelium     switches to a microvascular phenotype during angiogenesis in     collagen gel culture of rat aorta. Atherosclerosis: 95:191-199. -   Nicosia R F, Nicosia S V, Smith M. 1994b, Vascular endothelium     growth factor, platelet-derived growth factor, and insulin-like     growth factor-1 promote rat aorta. Atherosclerosis in vitro. Am J     Pathol 145:1023-1029. -   Nicosia R F, Ottinetti A. 1990. Modulation of microvascular growth     and morphogenesis by reconstituted basement membrane gel in     three-dimensional cultures of rat aorta: a comparative study of     angiogenesis in matrigel, collagen, fibrin, and plasma clot. In     Vitro Cell Dev Biol 26:119-128. -   Nicosia R F, Tchao Leighton J. 1982. Histotypic angiogenesis in     vitro: light microscopic, ultrastructural, and radioautographic     studies. In Vitro 18:538-549. -   Nicosia R F Tchao R, Leighton J. 1983. Angiogenesis-dependent tumor     spread in reinforced fibrin clot culture. Cancer Res 43:2159-2166. -   Nicosia R F, Tuszynski G P. 1994. Matrix-bound thrombospondin     promotes angiogenesis in vitro. J Cell Biol 124:183-193. -   Passaniti A, Taylor R M, Pili R, Guo Y, Long P V, Haney J A, Pauly R     R, Grant D S, Martin G R. 1992. A simple, quantitative method for     assessing angiogenesis and antiangiogenic agents using reconstituted     basement membrane, heparin, and fibroblast growth factor. Lab Invest     67:519-528. -   Pepper M S, Montesano R, Vassalli J D, Orci L. 1991. Chondrocytes     inhibit endothelial sprout formation in vitro: evidence for     involvement of a transforming growth factor-beta. J Cell A Physiol     146:170-179. -   Rosen E M, Meromsky L, Setter E, Vinter D W, Goldberg I D. 1990.     Quantitation of cytokine-stimulated migration of endothelium and     epithelium by a new assay using microcarrier beads. Exp Cell Res     186:22-31. -   Sage E H, Vernon R B. 1994. Regulation of angiogenesis by     extracellular matrix: the growth and the glue. J Hypertens Suppl     12:S145-152. -   Vernon R B, Angello J C, Iruela-Arispe M L, Lane T F, Sage     E H. 1992. Reorganization of basement membrane matrices by cellular     traction promotes the formation of cellular networks in vitro. Lab     Invest 66:536-547. -   Vernon R B, Gooden M D. 2002. New technologies in vitro for analysis     of cell movement on or within collagen gels. Matrix Biol 21:661-669. -   Vernon R B, Lara S L, Drake C J, Iruela-Arispe M L, Angello J C,     Little C D, Wight T N, Sage E H. 1995. Organized type I collagen     influences endothelial patterns during “spontaneous angiogenesis in     vitro”: planar cultures as models of vascular development. In Vitro     Cell Dev Biol Anim 31:120-131. -   Vernon R B. Sage E H. 1999. A novel, quantitative model for study of     endothelial cell migration and sprout formation within     three-dimensional collagen matrices. Microvasc Res 57:118-133. -   Villaschi S, Nicosia R F. 1993. Angiogenic role of endogenous basic     fibroblast growth factor released by rat aorta after injury. Am J     Pathol 143:181-190. 

1. A method for creating networks of perfusable microvessels in vitro, said method comprising: drawing a mandrel through a matrix to form a channel through the matrix; injecting cells into the channel; incubating the matrix to allow the cells to attach inside the channel; perfusing the channel to remove unattached cells to create a parent vessel within the channel, where the parent vessel includes a perfusable hollow channel lined with cells in the matrix; inducing the parent vessel to create sprouts into the surrounding matrix so as to form a microvessel network; and subjecting the microvessel network to luminal perfusion through the parent vessel.
 2. The method of claim 1, wherein more than one channel is formed by a plurality of mandrels, where the mandrels comprise capillary tubes and at least two parent vessels are induced to create sprouts that anastomoze to form a microvessel network.
 3. The method of claim 2, wherein the at least two parent vessels comprise multidimensional arrays of perfusable vessels.
 4. The method of claim 1, wherein perfusing the channel employs at least one of a perfusate comprising oxygenated cell growth medium free of serum and angiogenic or angiostatic substances, an oxygenated cell growth medium supplemented with serum, at least one of angiogenesis influencing compounds, an oxygenated physiological salt solution, oxygenated blood, blood components, blood substitutes, an un-oxygenated perfusate where oxygenation of the system is achieved by diffusion through the matrix, at least one of angiogenic and angiostatic compounds added to a perfusate, and at least one of angiogenic and angiostatic compounds in the matrix.
 5. The method of claim 1, wherein the cells comprise genetically modified cells that release products into a perfusate or into the matrix.
 6. The method of claim 1, wherein the matrix comprises material selected from the group consisting of fibrin, collagen, gelatin gelled basement membrane, agar, agarose, aliginate, basement membrane proteins, silica gel, cells and combinations thereof.
 7. The method of claim 1, wherein cells are deposited into the matrix channel by at least a selected one method of prior attachment to the mandrel, by injection into the matrix channel after withdrawal of the mandrel, and by a combination of prior attachment to the mandrel and also by injection into the matrix.
 8. The method of claim 1, wherein the mandrel is removed from the matrix by at least a selected one method of extraction and decomposition.
 9. The method of claim 1, wherein the cells are selected from the group consisting of endothelial cells, smooth muscle cells, pericytes, human cells, animal cells, plant cells, stem cells, muscle cells, liver cells, kidney cells, lung cells, skin cells, epithelial cells and genetically modified cells.
 10. The method of claim 1, wherein the matrix is populated with cells selected from the group consisting of endothelial cells, smooth muscle cells, pericytes, human cells, animal cells, plant cells stem cells, muscle cells, liver cells, kidney cells, lung cells, skin cells, epithelial cells and genetically modified cells.
 11. The method of claim 1, wherein a fragment of healthy or diseased tissue is embedded into the matrix.
 12. The method of claim 1, wherein a fragment of cancer tissue is embedded into the matrix.
 13. The method of claim 1 wherein a fluid perfusate is re-routed through the capillaries by decreasing the flow into one parent vessel, and increasing the resistance in a second parent vessel that is connected to the first one by one or more sprouts so that the perfusate is driven from the vessel with higher pressure to the vessel with lower pressure.
 14. The method of claim 1 wherein the microvessel network comprises a selected one of a bioartificial microvessel, patent endothelial cell tubes, and smooth muscle cell tubes.
 15. The method of claim 1 wherein microvessel networks are comprised of normal or genetically modified cells that release factors into the perfusate.
 16. The method of claim 1, wherein perfusing the channel includes using normal or genetically modified cells to release factors into a perfusate.
 17. A method for the creation of endothelial parent vessels from human vascular endothelial cells in vitro in a culture perfusion device (CPD) including a collagen chamber, a plurality of inlet ports, at least one capillary tube, and at least one outlet port comprising: injecting a collagen solution into the collagen chamber through a syringe needle until the chamber is filled with collagen; perfusing the CPD by filling the inlet ports and sequentially priming the plurality of inlet ports, and the outlet ports; creating at least one perfusable channel in the collagen chamber; injecting a concentrated suspension of endothelial cells into the inlet ports; injecting the endothelial cells into the at least one perfusable channel; incubating the CPD to allow the endothelial cells to attach to the walls of the at least one perfusable channel; distributing the cells within the CPD; perfusing the at least one perfusable channel to form at least one parent vessel having homogeneous monolayers of cells.
 18. A culture perfusion device for creating networks of perfusable microvessels in vitro comprising: means for drawing a mandrel through a matrix to form a channel through the matrix; means for injecting cells into the channel, the channel having an inner wall; means for incubating the matrix to allow the cells to attach to the inner wall; means for perfusing the channel to remove unattached cells to create a parent vessel, where the parent vessel includes a perfusable hollow channel lined with cells in the matrix; means for inducing the parent vessel to create sprouts into the surrounding matrix so as to form a microvessel network; and means for subjecting the microvessel network to luminal perfusion through the parent vessel. 